PHB granules are attached to the nucleoid via PhaM in Ralstonia eutropha
- Andreas Wahl†1,
- Nora Schuth†1,
- Daniel Pfeiffer1,
- Stephan Nussberger2 and
- Dieter Jendrossek1Email author
© Wahl et al.; licensee BioMed Central Ltd. 2012
Received: 6 September 2012
Accepted: 9 November 2012
Published: 16 November 2012
Poly(3-hydroxybutyrate) (PHB) granules are important storage compounds of carbon and energy in many prokaryotes which allow survival of the cells in the absence of suitable carbon sources. Formation and subcellular localization of PHB granules was previously assumed to occur randomly in the cytoplasm of PHB accumulating bacteria. However, contradictionary results on subcellular localization of PHB granules in Ralstonia eutropha were published, recently.
Here, we provide evidence by transmission electron microscopy that PHB granules are localized in close contact to the nucleoid region in R. eutropha during growth on nutrient broth. Binding of PHB granules to the nucleoid is mediated by PhaM, a PHB granule associated protein with phasin-like properties that is also able to bind to DNA and to phasin PhaP5. Over-expression of PhaM resulted in formation of many small PHB granules that were always attached to the nucleoid region. In contrast, PHB granules of ∆phaM strains became very large and distribution of granules to daughter cells was impaired. Association of PHB granules to the nucleoid region was prevented by over-expression of PhaP5 and clusters of several PHB granules were mainly localized near the cell poles.
Subcellular localization of PHB granules is controlled in R. eutropha and depends on the presence and concentrations of at least two PHB granule associated proteins, PhaM and PhaP5.
Polyhydroxyalkanoates (PHA) are intracellular storage materials of carbon and energy in many prokaryotes. Ralstonia eutropha is the most prominent and best-studied poly(3-hydroxybutyrate (PHB) accumulating bacterium [1–3]. The results of 25 years of research on biosynthesis, maintenance, intracellular degradation (mobilization) and application of PHA meanwhile provide a good picture on the structure and components of PHB granules. PHB granules are composed of an amorphous polymer core that is enclosed by a dense proteinaceous surface layer (for reviews see [4–13]). Polymer and surface layer constitute a multifunctional complex for which the term carbonosomes has been proposed . It is still an open question whether phospholipids [15, 16] are part of the PHB granule surface layer in vivo or whether they represent an in vitro preparation artifact that occurs upon cell lysis in course of the isolation process of so-called native PHB granules.
Six types of proteins constitute the proteinaceous PHB surface layer in R. eutropha: (i) the PHB synthase (PhaC1) is the key enzyme of PHB synthesis and catalyses the polymerization process of 3-hydroxybutyryl-CoA provided by the central metabolism [9, 17, 18]. The function of a second - catalytically inactive - PHB synthase, PhaC2  is unknown. However, PhaC2 principally has the capacity to bind to PHB granules in vivo ; (ii) phasin proteins (PhaPs), in particular PhaP1, cover most parts of the granule surface and prevent coalescence of granules [20–23]; (iii) PHB depolymerases (PhaZs) are important for reutilization (mobilization) of the polymer during times of starvation [24–28]; (iv) oligomer hydrolases (PhaZb, PhaZc, alternative designation PhaYs) are involved in cleavage of intermediately formed 3-hydroxybutyrate (3HB) oligomers during mobilization ; (v) regulatory proteins (PhaRs) regulate expression of selected phasin genes [30, 31] and (vi) PhaM represents the prototype of a recently discovered novel type of PHB granule associated protein that has phasin properties but also can bind to DNA .
However, despite this considerable amount of knowledge it is still an open question whether PHB granules are formed randomly within the cytoplasm or whether localization of PHB granules is controlled by the bacteria. Several studies using fluorescence microscopy (FM) [33–35] and transmission electron microscopy (TEM) [36, 37] were performed in the last decade to address this question. However, the results of these studies were inconsistent. While FM analysis of PHB granule formation in different PHB accumulating species suggested a non random localization of “early” PHB granules in the cell periphery of these species [14, 33, 34], investigation of PHB granule formation in R. eutropha by TEM suggested that PHB granules are formed predominantly in the cell centre near dark stained “mediation elements” [36, 37]. Electron cryotomography recently revealed that in R. eutropha PHB granules at different stages of PHB accumulation are localized more or less in the cell center whereas a preferential formation of PHB granules in the cell periphery has not been observed . The reason why FM and TEM resulted in apparently contradicting results remained unclear although the studies were performed with the same wild type strain. In recent studies of our laboratory we showed that PhaM can bind to PHB, to phasin PhaP5, to PHB synthase PhaC1 and to DNA [22, 32]. Consequently, we decided to reinvestigate PHB granule formation and intracellular localization in R. eutropha wild type and in mutants with altered expression of PhaP5 or PhaM. Our results show that PHB granules are localized in close contact to the nucleoid if PhaM is present and are detached from the nucleoid when PhaP5 is over-expressed.
Results and discussion
Time course of PHB granule formation in R. eutropha HF39 and H16
To study the formation and localization of PHB granules in R. eutropha we used R. eutropha strains H16 and HF39. Both strains have wild type properties with respect to PHB metabolism and easily form PHB granules during growth on rich media such as NB medium media. Strain HF39 is a spontaneous streptomycin resistant mutant of strain H16 and has often been used in place of strain H16 in conjugation experiments because of simplified counter selection of the donor . In this study, the same results were obtained for both strains with the exception that strain HF39 grew slightly slower and produced in average a lower number of PHB granules than strain H16.
Although R. eutropha strains H16 and HF39 intermediately accumulated PHB during growth on NB-medium more than 95% of the cells were free of PHB granules in the stationary growth phase after 24 h. Cells that still had PHB granules after this time period (<5%) often were division-inhibited (cells > 10 μm in length) and many of them were dead as revealed by staining with propidium iodide (images not shown). In conclusion, most living cells of the late stationary growth phase of R. eutropha on NB-medium were free of accumulated PHB.
Figure 1 shows representative images of thin sections of R. eutropha H16 at zero time. The cells harvested straight after transfer to fresh medium were rather short rods of about 0.9 μm in length and 0.5 μm in width. Most cells were free of any electron-transparent inclusions. Shortening of cells and consumption of previously accumulated PHB is a typical response of R. eutropha to stationary growth phase conditions after growth in NB medium. Despite the fixation procedure of the cells with formaldehyde and glutardialdehyde the cytoplasm often appeared more or less contracted (see arrowheads in Figure 1). This condensing effect of the cytoplasm was stronger in stationary phase cells compared to exponentially growing cells and indicated that the cells become weak in the stationary phase and do not resist the preparation procedure that well. Changing of the fixation conditions, e. g. by increasing the total aldehyde concentration up to 2% and variation of the agar temperature used for embedding of the cells between 46 and 60°C did not prevent formation of preparation artefacts of stationary R. eutropha cells such as plasmolysis of fixed cells.
The genomic DNA of the cells denatures during the fixation process and can be identified in stained thin sections by the different degree of staining intensity in comparison to the cytoplasm (see short arrows in Figure 1) [40, 41]. In some cells the denatured nucleoids were more intensively stained than in others (e. g. right cell of Figure 1 in comparison to the middle cell). Occasionally (1 to 5% of all cells at zero time), stationary cells revealed small circular structures of about 50–100 nm in diameter with light staining. This structure is likely a remains of small PHB granules (see long arrow in the left cell of Figure 1). PHB is a hydrophobic material and does not bind uranyl acetate or lead citrate that was added to increase the contrast of organic materials in TEM pictures. PHB granules therefore have an electron-transparent appearance. In case of very small PHB granules the diameters of the granules can be smaller than the thickness of a thin-section in transmission electron microscopy. In such cases, or if only a portion of a PHB granule is present within the volume of a thin-section, the appearance of the granules is not a complete “white” but “light grey”. This can be explained by the presence of stained material that was bound to materials of the cytoplasm above or below the granule. In contrast, large PHB granules have a diameter of 300 to 500 nm and are likely to span the complete volume of a thin-section. Large PHB granules therefore appear “white” in TEM images (see large globular structures in Figure 2). Remarkably, the PHB granule visible in Figure 1 (left cell) seems to be attached to the nucleoid region. No difference was observed between strain H16 and strain HF39 at zero time.
When cells were investigated that had been grown under PHB permissive conditions for 10 min to 1 hour many cells harboured one or two PHB granules (Figure 2). All granules were in contact to the nucleoid region. The size of the granules ranged between less than 100 and ≈ 300 nm within the first hour of growth. In cells that harboured two PHB granules the granules mostly were located at opposite sites of the nucleoid region. This observation is in line with previous observations made by fluorescence microscopy (Figure 1C of ).
When cells were investigated that had been grown for >1 h permissive for PHB synthesis the number and size of the granules further increased. Strain H16 accumulated in average more granules (up to 12) than strain HF39 (1 to 4). Since the diameter of accumulated PHB granules increased by time the volume of the granules also increased and the association of the granules with the nucleoid became less obvious and could not be differentiated from nucleoid exclusion; however it should be noted that for all cells shown in Figure 2, in which PHB granules and the nucleoid were visible, an association of the granules with the nucleoid is evident. In conclusion, the data suggest that PHB granules are rapidly formed under permissive conditions (within 10 min) and apparently are attached to the nucleoid region. Since PhaM binds to both DNA and PHB we speculated that PhaM is responsible for the association of PHB granules with the nucleoid (see below).
Time course of formation and subcellular localization of PHB granules in R. eutropha that over-express PhaM
PhaM represents a new type of PHB granule associated protein and has multiple functions. It had been identified by its in vivo interaction with PHB synthase PhaC1 in a two-hybrid screening assay . FM analysis revealed that PhaM is not only able to bind to PHB granules but also to the nucleoid region in R. eutropha. Moreover, purified PhaM was able to bind to genomic DNA in vitro as indicated in gel mobility shift experiments. To investigate the effect of PhaM on PHB granule formation the phaM gene was over-expressed constitutively from the phaC1 promotor. Figure 3 shows the time course of PHB granule formation in the PhaM-over-expressing transconjugant of R. eutropha H16 and HF39. No difference in number, size or localization of PHB granules was found when PhaM-over-expressing cells were compared with eYfp-PhaM over-expressing cells and confirmed that the presence of an eYfp tag did not change subcellular localization of fusion proteins. Most cells were free of PHB granules at zero time and the nucleoid region could be differentiated from the cytoplasm by the different degree of adsorbed staining material similar to wild type cells. PHB granules appeared already after 10–20 min of incubation under PHB permissive conditions. At later time points the number of PHB granules strongly increased up to several dozens. The granules were considerably smaller in diameter (< 100 nm) compared to wild type cells at all stages of growth and the granule size increased only little after longer incubation times at PHB permissive conditions. Remarkably, the granules were not randomly distributed in the cells but were exclusively in contact with or in close neighbourhood to the nucleoid. The PHB granules covered the complete surface of the nucleoid region in some cells. Occasionally, long cells were observed that apparently were inhibited in cell division (Figure 4, 3 h). Such cells harboured several well-separated nucleoid regions each of which was decorated with a high number of attached PHB granules resulting in the impression of “raspberries” within the cells. Free PHB granules, i.e. PHB granules that were not in contact to the nucleoid region were not observed. Apparently, constitutive over-expression of phaM resulted in formation of an increased number of small and nucleoid-attached PHB granules.
If PhaM is responsible for the formation of small granules and for the close contact to the nucleoid region, deletion of phaM should have a phenotype. In fact, R. eutropha ∆phaM cells accumulated only very few (0–2) PHB granules that were significantly larger in diameter than those of the phaM over-expressing mutant or of the wild type (Figure 5). Since the diameters of PHB granules of the ∆phaM strain were considerably larger even at early time points a precise analysis whether or not the granules were attached to the nucleoid region was difficult. In most ∆phaM cells the PHB granules were still located close to the nucleoid; however, at least in some cells a detachment of PHB granules from the nucleoid region could not be excluded for the wild type or for the phaM over-expressing strain. A clear decision whether the absence of PhaM resulted in detachment from the nucleoid can, however, not be made. Since R. eutropha expresses at least one other protein with DNA-binding and PHB-binding property (PhaR) [30, 31] it might be that PhaR also contributes to association of PHB with DNA. In summary, our data on mutants with altered expression of PhaM clearly show that number, diameter and subcellular localization of PHB granules depends on the presence and concentration of PhaM.
Time course of formation and localization of PHB granules in R. eutropha over-expressing PhaP5
As in the case of PhaM, no difference in number, size and localization of PHB granules was observed for the over-expressed eYfp-PhaP5 fusion in comparison to over-expression of PhaP5 alone. Growth and accumulation of PHB were similar in the recombinant strains as in the wild type. However, when the time-course of PHB granule formation and localization was investigated by TEM-analysis remarkable differences to the wild type were observed for the PhaP5 over-expressing strains (Figure 6): PHB granules were formed in aggregated clusters of in average 2–6 granules in most cells near both cell poles of the rod-shaped cells. These clusters could not be resolved by FM-analysis (Nile red staining) and resulted in the impression of only two (large) PHB granules near the cell poles (Figure 7). The number of individual granules visible in TEM images was increased but the diameter was decreased compared to wild type granules. In most cells, the PHB granule clusters or at least individual PHB granules of a cluster were clearly detached from the nucleoid region (see arrowheads in Figure 6). In conclusion, over-expression of PhaP5 has an impact on number, size and localization of PHB granules and leads to detachment of the granules from the nucleoid. This can be explained by binding of over-expressed PhaP5 to PhaM molecules thus preventing PhaM from binding to DNA and/or to PhaC. Alternatively, a competitive displacement of PhaM molecules from PHB granules surface by over-expressed PhaP5 could be responsible for the phenotype. Number and localization of PHB granules in a ∆phaP5 strain were, however, not significantly changed in comparison to wild type (data not shown).
Our data clearly show that formation and localization of PHB granules occurs not randomly but is specifically controlled in R. eutropha. Other examples of species with non-random localization of PHB granules are Rhodospirillum rubrum, Haloquadrata walsbyi, Azotobacter vinelandii, Beijerinckia indica, Caryophanon latum and Hyphomicrobium facile (supplementary material of ). However, we do not know whether attachment of PHB or PHA granules to the DNA is a general feature of PHB or PHA accumulating bacteria. PHB granules in R. eutropha are attached to the nucleoid via PhaM. Our conclusion is supported by previous TEM analysis of others if the “dark-stained mediation elements” are interpreted as denatured chromosomal DNA [36, 37]. The reason why the authors of these studies did not observe PHB granules in the cell periphery in thin sections might be explained by differences in growth conditions of the bacteria: they used a mineral salts-based PHB production medium with high carbon but low nitrogen source; first samples were taken after 2.5 h of incubation. At this time the nitrogen source should have been consumed resulting in strong PHB accumulation but also in stop of nucleoid replication. In our experiments, the cells were subjected to high carbon (gluconate) and high nitrogen (nutrient broth) sources resulting in cell growth AND PHB granule formation. Active separation of the replicated chromosomes with bound PHB granules resulted in formation of cells with PHB granules that often localized near the cell poles. Therefore, the results of Tian et al. are not contradictionary to our findings. Moreover, our data are also in agreement with recent biochemical work of the same group in which an association of PHB and PhaM was confirmed .
Over-expression of phasin PhaP5 leads to detachment of PHB granules from the nucleoid probably because of competitive binding to PhaM. However, the expression level of PhaP5 in R. eutropha wild type is only low as indicated by transcriptome data . An involvement of additional proteins in subcellular localization can not be excluded.
Bacterial strains, plasmids and culture conditions
Strains and plasmids used in this study
Source or reference
Escherichia coli JM109
E. coli S17-1
Ralstonia eutropha H16
Wild type strain, PHB accumulation
Ralstonia eutropha HF39
Streptomycin resistant derivate of H16
R. eutropha H16 ∆phaP5
Chromosomal deletion of phaP5
R. eutropha H16 ∆phaM
Chromosomal deletion of phaM
Source or reference
broad host range vector
Constitutive eYfp over-expression
pBBR1MCS-2- P phaC -eyfp-phaP5
Fusion of PhaP5 to C-terminus of eYfp
pBBR1MCS-2- P phaC –eyfp-phaM
Fusion of eYfp to N-terminus to PhaM
pBBR1MCS-2- P phaC –phaP5
Constitutive over-expression of PhaP5
pBBR1MCS-2- P phaC –phaM
Constitutive over-expression of PhaM
Preparation of cells for TEM analysis
Fixed cells were washed three times with 1 mL PBS+10 mM glycine to remove excess of aldehydes. An aliquot of the cells was taken for fluorescence microscopy. The cell pellet of the third washing step was resuspended with PBS in a final volume of 100 μL. Cells were added to an equal volume of a 2% (in PBS) agar solution (prewarmed to 50°C in a 2 mL Eppendorf tube using prewarmed pipette tips), mixed and centrifuged for ≈ 10 s at room temperature to obtain a high cell concentration at the bottom of the agar. The agar was cooled on ice. The agar block containing fixed R. eutropha cells was removed from the Eppendorf cups using a steam of nitrogen gas applied with a capillare to the bottom of the Eppendorf tube and was cut into more or less cube-shaped pieces (≈ 1 mm3). The cells were dehydrated by incubation of the agar cubes in a series of subsequent dehydration steps using: 15% methanol on ice for 15 min, 30% ethanol for 30 min on ice, and subsequent 30 min incubation steps at - 20°C using 50%, 70%, 96% and 100% (twice) ethanol. Subsequently, the dehydrated cubes were transferred to a solution consisting of ethanol and LR white resin (3:1) and incubated at room temperature for 2 h before the solution was exchanged against pure LR white and incubated at 4°C for at least 2 h (or overnight). Several cubes were then transferred to gelatine capsules, filled with LR white and polymerized at 50°C (or 60°C) for 30 h (or 24 h). The solidified samples were stored in the dark at room temperature until use. Thin sections were prepared using a Leica Ultracut microtome and glass or diamond knifes. Slices of appropriate thickness were transferred to copper grids and stained with uranyl acetate (2%) and lead citrate according to Reynolds . EM images of thin sections were recorded using a Tecnai G2 Sphera electron transmission microscope (FEI) equipped with a large area TemCam F224HD CCD camera (TVIPS). The microscope was operated at 120 kV.
Over-expression of PhaM and PhaP5
The phaM and phaP5 genes were cloned under control of the (in R. eutropha) constitutively expressed phaC promoter in pBBR1MCS2-PphaC (Table 1). The primer sequences (PhaP5_f_NdeI GGGAATTCCATATGGCCACGCCTCCCAATCC, PhaP5_r_BamHI CGGGATCCCTAGCCCTTGGATTTCGGCTTG and PhaM_f_NdeI GGGAATTCCATATGTTCGGACAGATTCCCGATTTC, PhaM_r_BamHI CGGGATCCTCAGGCTGCGCTGCTG) were used for amplification of phaP5 and phaM. The respective PCR products were ligated into pBBR1MCS2-PphaC via NdeI & BamHI sites and cloned in E. coli JM109. Integration and DNA sequence of cloned genes were verified by determination of the DNA sequence. Plasmids were conjugatively transferred from. E. coli S17-1 harbouring the plasmid of interest were conjugatively transferred to R. eutropha H16 or strain HF39 by selection on mineral salts medium supplemented with 0.5% fructose and 350 μg ml-1 kanamycin as described previously [22, 32]. The respective strains were grown on NB medium supplemented with 0.2% gluconate as described above. Strains with constitutively expressed fusions of PhaM or PhaP5 with eYfp were expressed in an analogue way.
Molecular biological experiments were performed by standard methods . Fluorescence microscopical analysis of R. eutropha cells harbouring fusion proteins with eYfp in the absence or presence of Nile red was conducted as described previously . Construction of chromosomal deletions of phaP5 and of phaM in R. eutropha strains has been described elsewhere [22, 32] using a sacB-based system for selection of double cross-over events. In all cases the mutations were verified by PCR-amplification of the mutated gene locus and by determination of the amplified DNA sequence. Only clones with correct DNA sequence were used.
This work was supported by a grant of the Deutsche Forschungsgemeinschaft to D.J. TEM experiments of this work would not have been possible without technical support by M. Schweikert and B. Nitschke that is greatly acknowledged.
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